|Publication number||US8053192 B2|
|Application number||US 12/012,613|
|Publication date||Nov 8, 2011|
|Priority date||Feb 2, 2007|
|Also published as||EP2121983A2, US8182989, US8822150, US20090233802, US20120015823, US20120316072, US20140329698, WO2008093098A2, WO2008093098A3|
|Publication number||012613, 12012613, US 8053192 B2, US 8053192B2, US-B2-8053192, US8053192 B2, US8053192B2|
|Inventors||Helen Bignell, Louise Fraser, Niall Anthony Gormley|
|Original Assignee||Illumina Cambridge Ltd.|
|Export Citation||BiBTeX, EndNote, RefMan|
|Patent Citations (102), Non-Patent Citations (102), Referenced by (26), Classifications (7), Legal Events (4)|
|External Links: USPTO, USPTO Assignment, Espacenet|
The present application claims priority from U.S. Provisional Application 60/899,221, filed Feb. 2, 2007. Applicants claim the benefits of priority under 35 U.S.C. §119 as to the Provisional Application, the entire disclosure of which is incorporated herein by reference in its entirety.
This invention was made with government support under grant number U54 HG003067 awarded by the National Institutes of Health. The government has certain rights in this invention.
The invention relates to methods for indexing samples during the sequencing of polynucleotide templates, resulting in the attachment of tags specific to the source of each nucleic acid sample such that after a sequencing run, both the source and sequence of each polynucleotide can be determined. Thus, the present invention pertains to analysis of complex genomes (e.g., human genomes), as well as multiplexing less complex genomes, such as those of bacteria, viruses, mitochondria, and the like.
Several publications and patent documents are referenced in this application in order to more fully describe the state of the art to which this invention pertains. The disclosure of each of these publications and documents is incorporated by reference herein.
Advances in the study of biological molecules have been led, in part, by improvement in technologies used to characterise the molecules or their biological reactions. In particular, the study of the nucleic acids DNA and RNA has benefited from developing technologies used for sequence analysis.
The study of complex genomes, in particular, the search for the genetic basis of disease in humans requires genotyping on a massive scale. Screens for numerous genetic markers performed on populations large enough to yield statistically significant data are needed before associations can be made between a given genotype and a particular disease. However large-scale genotyping is demanding in terms of the cost of both materials and labour involved, and the time taken to perform the study, especially if the methodology employed involves separate serial analysis of individual DNA samples. One shortcut is to pool DNA from many individuals and to determine parameters such as the ratio of changes at certain positions in the genome. Such measurements of ‘allele frequency’ in the pool of samples can be used to correlate the relationship between the changes in the genome sequence and the occurrence of a disease. Hence, an association study involving 1000 patients would in theory only necessitate a ‘one-pot’ reaction for each genetic change. Pooling therefore represents an effective technique for analysing large quantities of samples in a facile manner.
One disadvantage of pooling samples prior to analysis is that information pertaining to individual DNA samples is lost; only global information such as allele frequencies is gathered, as there is no easy method for discerning which individuals gave rise to a particular genotype. An ability to genotype large populations in a small number of reactions, while retaining the information relating to the source of the individual samples, would yield the information content of a full non-pooled population screen in the time and at the cost of a pooled reaction.
Several of the new methods employed for high throughput DNA sequencing (Nature. 437, 376-380 (2005); Science. 309, 5741, 1728-1732 (2005)) rely on a universal amplification reaction, whereby a DNA sample is randomly fragmented, then treated such that the ends of the different fragments all contain the same DNA sequence. Fragments with universal ends can be amplified in a single reaction with a single pair of amplification primers. Separation of the library of fragments to the single molecule level prior to amplification ensures that the amplified molecules form discrete populations that can then be further analysed. Such separations can be performed either in emulsions (Nature. 437, 376-380 (2005); Science. 309, 5741, 1728-1732 (2005)), or on a surface (Nucleic Acids Research 27, e34 (1999); Nucleic Acids Research 15, e87 (2000)).
WO 98/44151 and WO 00/18957 both describe methods of forming polynucleotide arrays based on ‘solid-phase’ nucleic acid amplification, which is a bridging amplification reaction wherein the amplification products are immobilised on a solid support in order to form arrays comprised of nucleic acid clusters or ‘colonies’. Each cluster or colony on such an array is formed from a plurality of identical immobilised polynucleotide strands and a plurality of identical immobilised complementary polynucleotide strands. The arrays so-formed are generally referred to herein as ‘clustered arrays’ and their general features will be further understood by reference to WO 98/44151 or WO 00/18957, the contents of both documents being incorporated herein in their entirety by reference.
In common with all amplification techniques, solid-phase bridging amplification requires the use of forward and reverse amplification primers which include ‘template-specific’ nucleotide sequences which are capable of annealing to sequences in the template to be amplified, or the complement thereof, under the conditions of the annealing steps of the amplification reaction. The sequences in the template to which the primers anneal under conditions of the amplification reaction may be referred to herein as ‘primer-binding’ sequences.
Certain embodiments of the methods described in WO 98/44151 and WO 00/18957 make use of ‘universal’ primers to amplify templates comprising a variable template portion that it is desired to amplify flanked 5′ and 3′ by common or ‘universal’ primer binding sequences. The ‘universal’ forward and reverse primers include sequences capable of annealing to the ‘universal’ primer binding sequences in the template construct. The variable template portion, or ‘target’ may itself be of known, unknown or partially known sequence. This approach has the advantage that it is not necessary to design a specific pair of primers for each target sequence to be amplified; the same primers can be used for amplification of different templates provided that each template is modified by addition of the same universal primer-binding sequences to its 5′ and 3′ ends. The variable target sequence can therefore be any DNA fragment of interest. An analogous approach can be used to amplify a mixture of templates (targets with known ends), such as a plurality or library of target nucleic acid molecules (e.g. genomic DNA fragments), using a single pair of universal forward and reverse primers, provided that each template molecule in the mixture is modified by the addition of the same universal primer-binding sequences.
DNA from more than one source can be sequenced on an array if each DNA sample is first tagged to enable its identification after it has been sequenced. Many low scale DNA-tag methodologies already exist, for example fluorescent labelling (Haughland, Handbook of Fluorescent Probes and Research Products, Invitrogen/Molecular Probes), but these are limited in scope to less than 10 or so reactions in parallel. DNA tags can be added to the ends of DNA fragments by cloning, of example as described in U.S. Pat. No. 5,604,097. The tags consist of eight four base ‘words’, where each word uses only three bases (A, T and C) in various combinations resulting in a total of 16,777,216 different tags that all have the same base pair composition and melting points. Such tags are used to label target molecules in a sample so that after an amplification reaction, each original molecule in the sample has a unique tag. The tags can then be used to ‘sort’ the sample onto beads containing sequences complementary to the tags such that each bead contains multiple copies of a single amplified target sequence (Brenner et al., (2000) Nature Biotechnology, 18, 630). In this application the tags are not sequenced, so the method does not provide a method of analysing targets from multiple samples, but rather a method of sorting a mixture of amplified templates from a single sample. The problem with enabling the method for individual samples rather than individual molecules is that the tags are synthesised in a combinatorial manner, meaning that all 16,777,216 different sequences are obtained in a single mixture in the same tube. Whilst this is ideal for treating one sample such that each individual molecule in the sample carries a different tag, it does not permit attachment of the same tag to every molecule in the sample.
DNA samples from multiple sources can, however, be tagged with different nucleic acid tags such that the source of the sample can be identified. Previous application WO05068656 describes the generic concept of indexing samples. In order to utilise this invention on arrays of amplified single molecule templates, for example as described in WO9844151, WO06099579 or WO04069849, it is advantageous to prepare the nucleic acids using the novel method described herein. The optimised DNA sample preparation techniques described herein are applicable to any method where the samples are amplified prior to sequencing. The DNA sample preparation techniques presented herein describe in detail the optimal placements of the sequencing primers and indexed tags within the DNA constructs to be sequenced.
The present inventors have developed methods for indexing samples, wherein the samples are amplified from isolated single template molecules. Using the techniques of the invention, it is possible to prepare a nucleic acid sample for a sequencing reaction wherein both the target sequence and the tag sequence can be determined.
In a first embodiment of the invention, a method is presented for sequencing nucleic acid sequences on an array and identifying subsets of nucleic acid sequences on an array, wherein each subset of nucleic acid sequences is isolated from a different source, wherein the method comprises the steps of:
In a second embodiment of the invention, a method is presented for sequencing nucleic acid sequences on an array and identifying subsets of nucleic acid sequences on an array, wherein each subset of nucleic acid sequences is isolated from a different source, wherein the method comprises the steps of:
In a third embodiment of the invention, a method is presented for sequencing nucleic acid sequences on an array and identifying subsets of nucleic acid sequences on an array, wherein each subset of nucleic acid sequences is isolated from a different source, wherein the method comprises the steps of:
In accordance with the first or second embodiment of the invention, sequencing can be performed in two separate reads. In accordance with the third embodiment of the invention, sequencing of the target fragment and the sample specific tag sequence can be performed in a single sequencing read.
With respect to the first, second, or third embodiments, the method encompasses a step wherein the pooled samples are amplified on a solid surface prior to sequencing. In a particular aspect, the solid surface on which amplification is performed is a collection of beads. In a more particular aspect, the collection of beads may be isolated as single beads in an emulsion.
With respect to the first, second, or third embodiments, the method encompasses a step wherein the array of immobilized fragments is amplified prior to sequencing to generate an amplified array. In a particular aspect, an amplified array so produced is a clustered array of amplified single molecules. Such clustered arrays may be formed, for example, by solid-phase nucleic acid amplification or isothermal solid-phase nucleic acid amplification.
The present method encompasses sequencing that involves cycles of ligation with labelled oligonucleotides or cycles of addition of nucleotides. In a particular aspect of the invention, the nucleotides are labelled. In a more particular aspect the nucleotides are labelled with fluorophores.
In an aspect of any of the first, second, or third embodiments of the invention, the sequencing step may be carried out on an array of immobilised beads.
A further aspect of the invention comprises a kit comprising a double stranded nucleic acid adapter and at least two different primer polynucleotides that carry a different tag sequence that does not hybridise to the adapter.
The present invention is directed to methods that advance techniques for nucleic acid analysis, such that target nucleic acids from a plurality of sources can be tagged with a unique, identifiable sequence of nucleic acid bases and then sequenced on a single array. As described herein, the presence of a characteristic nucleic acid sequence tag on an immobilised target molecule permits identification of the source of the target, concurrent with a sequence read from the target. This is a dramatic improvement over pre-existing array technologies which generally require a two-step process involving an initial sequencing step for sequencing the pooled nucleic acid targets, followed by a second analysis step wherein the source of the nucleic acid is determined.
The limitations of such pre-existing array technologies are evident in WO 98/44151 and WO 00/18957, for example, which both describe methods of nucleic acid amplification which allow amplification products to be immobilised on a solid support in order to form arrays comprised of clusters or “colonies” formed from a plurality of identical immobilised polynucleotide strands and a plurality of identical immobilised complementary strands. The nucleic acid molecules present in DNA colonies on the clustered arrays prepared according to these methods can provide templates for sequencing reactions, but to date only a single sequencing read can be obtained from each immobilised strand in each colony. The methods described herein allow for two or more reads on a single amplified strand, thereby allowing analysis of the tag sequence independently of the target sequence, and also allowing the possibility of a paired read from the opposite end of each fragment as well as a third read for the tag sequence. The methods also allow the preparation of constructs where the tag sequence is adjacent to the target sequence, and the tag and target are read in a single read, which again can be turned into a paired read methodology if desired.
As will be apparent to the skilled reader, references herein to a particular nucleic acid sequence may, depending on the context, also refer to nucleic acid molecules which comprise the nucleic acid sequence. Sequencing of a target fragment means that a read of the chronological order of bases is established. The bases do not need to be contiguous, although this is preferred, nor does every base on the entire fragment have to be sequenced.
The following passages describe different aspects of the invention in greater detail. Each aspect of the invention may be combined with any other aspect or aspects of the invention unless clearly indicated to the contrary. In particular, any feature indicated as being preferred or advantageous may be combined with any other feature of features indicated as being preferred or advantageous.
The terms ‘target nucleic acid sequence’, ‘target nucleic acid molecule’, ‘target nucleic acid’ and ‘target nucleic acid fragment’ may be used interchangeably to refer to nucleic acid molecules that it is desired to sequence on an array according to the invention. The target nucleic acid may be essentially any nucleic acid of known or unknown sequence. It may be, for example, a fragment of genomic DNA or cDNA. Sequencing may result in determination of the sequence of the whole, or a part of the target molecule. The targets can be derived from a primary nucleic acid sample that has been randomly fragmented. The targets can be processed into templates suitable for amplification by the placement of universal amplification sequences at the ends of each target fragment. The targets can also be obtained from a primary RNA sample by reverse transcription into cDNA.
As used herein, the term ‘polynucleotide’ refers to deoxyribonucleic acid (DNA), but where appropriate the skilled artisan will recognise that the method may also be applied to ribonucleic acid (RNA). The terms should be understood to include, as equivalents, analogs of either DNA or RNA made from nucleotide analogs and to be applicable to single stranded (such as sense or antisense) and double stranded polynucleotides. The term as used herein also encompasses cDNA, that is complementary or copy DNA produced from an RNA template, for example by the action of reverse transcriptase.
The primary polynucleotide molecules may originate in double-stranded DNA (dsDNA) form (e.g. genomic DNA fragments, PCR and amplification products and the like) or may have originated in single-stranded form, as DNA or RNA, and been converted to dsDNA form. By way of example, mRNA molecules may be copied into double-stranded cDNAs suitable for use in the method of the invention using standard techniques well known in the art. The precise sequence of the primary polynucleotide molecules is generally not material to the invention, and may be known or unknown.
In a particular embodiment, the primary polynucleotide molecules are RNA molecules. In an aspect of this embodiment, RNA isolated from specific samples is first converted to double-stranded DNA using techniques known in the art. In accordance with the present method, the double-stranded DNA is then tagged or indexed with a sample specific tag. Different preparations of such double-stranded DNA comprising sample specific tags can be generated, in parallel, from RNA isolated from different specific samples. Subsequently, different preparations of double-stranded DNA comprising different sample specific tags can be mixed, sequenced en masse, and the identity of each sequenced fragment determined with respect to the sample from which it was isolated/derived by virtue of the presence of a sample specific tag.
In a particular embodiment, the primary polynucleotide molecules are DNA molecules. More particularly, the primary polynucleotide molecules represent the entire genetic complement of an organism, and are genomic DNA molecules which include both intron and exon sequences (coding sequence), as well as non-coding regulatory sequences such as promoter and enhancer sequences. Although it could be envisaged that particular sub-sets of polynucleotide sequences or genomic DNA could also be used, such as, for example, particular chromosomes. Yet more particularly, the sequence of the primary polynucleotide molecules is not known. Still yet more particularly, the primary polynucleotide molecules are human genomic DNA molecules. The DNA target molecules may be treated chemically or enzymatically either prior to, or subsequent to any random fragmentation processes, and prior to or subsequent to the ligation of the adaptor sequences.
Methods of the invention are especially useful for the parallel sequencing of a large number of relative small samples in the same experiment. In a sequencing platform with a high degree of parallelism, it may be possible to analyse 50-100 million reads in the same experiment, each to a length of 50 bases or more. Thus it may easily be possible to determine more than 5 billion base pairs of sequence from a single experiment. For a genome of 100,000-1 million base pairs, this represents a much larger coverage of each base pair than is actually needed for accurate sequencing. This feature is even more pronounced for viral or mitochondrial genomes or collections of PCR fragments that may be 10,000 base pairs or less. For a 10 kB sample, sequenced in a run of 5 billion base pairs, each base pair will appear on average 500,000 times. For accurate sequencing, it may be desirable for each base pair to appear only 20 times, and thus it will be possible to sequence 25,000 10 kB fragments in the sequencing run. The use of 8 base pair tags gives a possibility of 48 (65536) different samples in the same experiment. For the sake of clarity, sequencing of the tags can be performed in a separate read from the sequencing of the target fragments, so the read length or accuracy of the read from the sample is not lowered by the need to sequence the tags.
For genome sizes of 1 mB, at a depth of 20×, it is possible to sequence 250 samples in a 5 billion base pair experiment. The 250 samples can be coded by as few as a four base tag, but extra bases may be added to ensure accurate analysis. Thus, the primary polynucleotide molecules may be a genome of any organism, but the methods of the present invention may be used to particular advantage when analysing smaller genomes, such as those of bacteria, viruses, mitochondria and the like, which have genome sizes in the regions of a few million base pairs or lower.
Random fragmentation refers to the fragmentation of a polynucleotide molecule in a non-ordered fashion by enzymatic, chemical or mechanical means. Such fragmentation methods are known in the art and utilise standard methods (Sambrook and Russell, Molecular Cloning, A Laboratory Manual, third edition). For the sake of clarity, generating smaller fragments of a larger piece of nucleic acid via specific PCR amplification of such smaller fragments is not equivalent to fragmenting the larger piece of nucleic acid because the larger piece of nucleic acid sequence remains in intact (i.e., is not fragmented by the PCR amplification). Moreover, random fragmentation is designed to produce fragments irrespective of the sequence identity or position of nucleotides comprising and/or surrounding the break. More particularly, the random fragmentation is by mechanical means such as nebulisation or sonication to produce fragments of about 50 base pairs in length to about 1500 base pairs in length, still more particularly 50-700 base pairs in length, yet more particularly 50-400 base pairs in length. Most particularly, the method is used to generate smaller fragments of from 50-150 base pairs in length.
Fragmentation of polynucleotide molecules by mechanical means (nebulization, sonication and Hydroshear for example) results in fragments with a heterogeneous mix of blunt and 3′- and 5′-overhanging ends. It is therefore desirable to repair the fragment ends using methods or kits (such as the Lucigen DNA terminator End Repair Kit) known in the art to generate ends that are optimal for insertion, for example, into blunt sites of cloning vectors. In a particular embodiment, the fragment ends of the population of nucleic acids are blunt ended. More particularly, the fragment ends are blunt ended and phosphorylated. The phosphate moiety can be introduced via enzymatic treatment, for example, using polynucleotide kinase.
In a particular embodiment, the target polynucleotide sequences are prepared with single overhanging nucleotides by, for example, activity of certain types of DNA polymerase such as Taq polymerase or Klenow exo minus polymerase which has a nontemplate-dependent terminal transferase activity that adds a single deoxynucleotide, for example, deoxyadenosine (A) to the 3′ ends of, for example, PCR products. Such enzymes can be utilised to add a single nucleotide ‘A’ to the blunt ended 3′ terminus of each strand of the target polynucleotide duplexes. Thus, an ‘A’ could be added to the 3′ terminus of each end repaired duplex strand of the target polynucleotide duplex by reaction with Taq or Klenow exo minus polymerase, whilst the adaptor polynucleotide construct could be a T-construct with a compatible ‘T’ overhang present on the 3′ terminus of each duplex region of the adaptor construct. This end modification also prevents self-ligation of both vector and target such that there is a bias towards formation of the combined ligated adaptor-target sequences.
The method of the invention utilises nucleic acid sequence tags as markers characteristic of the source of particular target molecules on the array. A nucleic acid sequence tag characteristic of the source is attached to each of the target molecules in each isolated sample before the sample is immobilised for sequencing. The tag is not itself formed by part of the target nucleic acid molecule, but becomes part of the template for amplification. Generally the tag will be a synthetic sequence of nucleotides which is added to the target as part of the template preparation step. Accordingly, a sample specific tag is a nucleic acid sequence tag which is attached to each of the target molecules of a particular sample, the presence of which is indicative of or is used to identify the sample or source from which the target molecules were isolated.
Preferably the nucleic acid sequence tag may be up to 20 nucleotides in length, more preferably 1-10 nucleotides, and most preferably 4-6 nucleotides in length. A four nucleotide tag gives a possibility of multiplexing 256 samples on the same array, a six base tag enables 4096 samples to be processed on the same array.
In the first embodiment of the invention, the tag sequences are introduced in a two step process involving ligation of an adaptor that is common to all samples and amplification with a tagged amplification primer. See
In each embodiment, the target nucleic acids of each specific fragmented sample are treated by first ligating identical adaptor polynucleotide molecules (‘mismatched adaptors’, the general features of which are defined below, and further described in copending application US 20070128624, the contents of which are incorporated herein by reference in their entirety) to the 5′ and 3′ ends of the target polynucleotide duplexes (which may be of known, partially known or unknown sequence) to form adaptor-target constructs and then carrying out an initial primer extension reaction in which extension products complementary to both strands of each individual adaptor-target construct are formed. The resulting primer extension products, and optionally amplified copies thereof, collectively provide a library of template polynucleotides. The term library refers to the collection of target fragments containing known common sequences at their 3′ and 5′ ends, and may also be referred to as a 3′ and 5′ modified library.
Depending on the embodiment of the invention, the adaptors may be universal for all samples, or one or both strands of the duplexes may carry the tag sequence to code or track the identity of the samples.
The adaptor polynucleotides used in the method of the invention are referred to herein as ‘mismatched’ adaptors because, as will be explained in detail herein, it is essential that the adaptors include a region of sequence mismatch, i.e., they must not be formed by annealing of fully complementary polynucleotide strands.
Mismatched adaptors for use in the invention are formed by annealing of two partially complementary polynucleotide strands so as to provide, when the two strands are annealed, at least one double-stranded region and at least one unmatched single-stranded region.
The ‘double-stranded region’ of the adaptor is a short double-stranded region, typically comprising 5 or more consecutive base pairs, formed by annealing of the two partially complementary polynucleotide strands. This term refers to a double-stranded region of nucleic acid in which the two strands are annealed and does not imply any particular structural conformation.
Generally it is advantageous for the double-stranded region to be as short as possible without loss of function. In this context, ‘function’ refers to the ability of the double-stranded region to form a stable duplex under standard reaction conditions for an enzyme-catalysed nucleic acid ligation reaction, which will be well known to the skilled reader (e.g. incubation at a temperature in the range of 4° C. to 25° C. in a ligation buffer appropriate for the enzyme), such that the two strands forming the adaptor remain partially annealed during ligation of the adaptor to a target molecule. It is not absolutely necessary for the double-stranded region to be stable under the conditions typically used in the annealing steps of primer extension or PCR reactions.
Since identical adaptors are ligated to both ends of each target molecule, the target sequence in each adaptor-target construct will be flanked by complementary sequences derived from the double-stranded region of the adaptors. The longer the double-stranded region, and hence the complementary sequences derived therefrom in the adaptor-target constructs, the greater the possibility that the adaptor-target construct is able to fold back and base-pair to itself in these regions of internal self-complementarity under the annealing conditions used in primer extension and/or PCR. It is, therefore, generally preferred for the double-stranded region to be 20 or less, 15 or less, or 10 or less base pairs in length in order to reduce this effect. The stability of the double-stranded region may be increased, and hence its length potentially reduced, by the inclusion of non-natural nucleotides which exhibit stronger base-pairing than standard Watson-Crick base pairs.
It is preferred, but not absolutely essential, for the two strands of the adaptor to be 100% complementary in the double-stranded region. It will be appreciated that one or more nucleotide mismatches may be tolerated within the double-stranded region, provided that the two strands are capable of forming a stable duplex under standard ligation conditions.
Adaptors for use in the invention will generally include a double-stranded region forming the ‘ligatable’ end of the adaptor, i.e. the end that is joined to a target polynucleotide in the ligation reaction. The ligatable end of the adaptor may be blunt or, in other embodiments, short 5′ or 3′ overhangs of one or more nucleotides may be present to facilitate/promote ligation. The 5′ terminal nucleotide at the ligatable end of the adaptor is phosphorylated to enable phosphodiester linkage to a 3′ hydroxyl group on the target polynucleotide.
The term ‘unmatched region’ refers to a region of the adaptor wherein the sequences of the two polynucleotide strands forming the adaptor exhibit a degree of non-complementarity such that the two strands are not capable of fully annealing to each other under standard annealing conditions for a primer extension or PCR reaction. The unmatched region(s) may exhibit some degree of annealing under standard reaction conditions for an enzyme-catalysed ligation reaction, provided that the two strands revert to single stranded form under annealing conditions in an amplification reaction.
It is to be understood that the ‘unmatched region’ is provided by different portions of the same two polynucleotide strands which form the double-stranded region(s). Mismatches in the adaptor construct can take the form of one strand being longer than the other, such that there is a single stranded region on one of the strands, or a sequence selected such that the two strands do not hybridise, and thus form a single stranded region on both strands. The mismatches may also take the form of ‘bubbles’, wherein both ends of the adaptor construct(s) are capable of hybridising to each other and forming a duplex, but the central region is not. The portion of the strand(s) forming the unmatched region are not annealed under conditions in which other portions of the same two strands are annealed to form one or more double-stranded regions. For avoidance of doubt it is to be understood that a single-stranded or single base overhang at the 3′ end of a polynucleotide duplex that subsequently undergoes ligation to the target sequences does not constitute an ‘unmatched region’ in the context of this invention.
The lower limit on the length of the unmatched region will typically be determined by function, for example, the need to provide a suitable sequence for binding of a primer for primer extension, PCR and/or sequencing. Theoretically there is no upper limit on the length of the unmatched region, except that in general it is advantageous to minimise the overall length of the adaptor, for example, in order to facilitate separation of unbound adaptors from adaptor-target constructs following the ligation step. Therefore, it is generally preferred that the unmatched region should be less than 50, or less than 40, or less than 30, or less than 25 consecutive nucleotides in length.
The precise nucleotide sequence of the adaptors is generally not material to the invention and may be selected by the user such that the desired sequence elements are ultimately included in the common sequences of the library of templates derived from the adaptors to, for example, provide binding sites for particular sets of universal amplification primers and/or sequencing primers. Additional sequence elements may be included, for example, to provide binding sites for sequencing primers which will ultimately be used in sequencing of template molecules in the library, or products derived from amplification of the template library, for example on a solid support.
Although the precise nucleotide sequence of the adaptor is generally non-limiting to the invention, the sequences of the individual strands in the unmatched region should be such that neither individual strand exhibits any internal self-complementarity which could lead to self-annealing, formation of hairpin structures, etc. under standard annealing conditions. Self-annealing of a strand in the unmatched region is to be avoided as it may prevent or reduce specific binding of an amplification primer to this strand.
The mismatched adaptors are preferably formed from two strands of DNA, but may include mixtures of natural and non-natural nucleotides (e.g. one or more ribonucleotides) linked by a mixture of phosphodiester and non-phosphodiester backbone linkages. Other non-nucleotide modifications may be included such as, for example, biotin moieties, blocking groups and capture moieties for attachment to a solid surface, as discussed in further detail below.
The adaptor constructs may contain exonuclease resistant modifications such as phosphorothioate linkages. Such modifications reduce the number of adaptor-dimers present in the library, since the two adaptors can not undergo ligation without removal of their non complementary overhangs. The adaptors can be treated with an exonuclease enzyme prior to the ligation reaction with the target, to ensure that the overhanging ends of the strands can not be removed during the ligation process. Treatment of the adaptors in this manner reduces the formation of the adaptor-dimers at the ligation step.
Ligation methods are known in the art and utilise standard methods (Sambrook and Russell, Molecular Cloning, A Laboratory Manual, third edition). Such methods utilise ligase enzymes such as DNA ligase to effect or catalyse joining of the ends of the two polynucleotide strands of, in this case, the adaptor duplex construct and the target polynucleotide duplexes, such that covalent linkages are formed. The adaptor duplex construct may contain a 5′-phosphate moiety in order to facilitate ligation to the target 3′-OH. The target contains a 5′-phosphate moiety, either residual from the shearing process, or added using an enzymatic treatment step, and has been end repaired, and optionally extended by an overhanging base or bases, to give a 3′-OH suitable for ligation. In this context, joining means covalent linkage of polynucleotide strands which were not previously covalently linked. In a particular aspect of the invention, such joining takes place by formation of a phosphodiester linkage between the two polynucleotide strands, but other means of covalent linkage (e.g. non-phosphodiester backbone linkages) may be used.
Optionally the combined ligated polynucleotide sequences and unligated adaptor polynucleotide constructs may be purified from any components of the ligation reaction, such as enzymes, buffers, salts and the like. Suitable purification methods are known in the art and utilise standard methods (Sambrook and Russell, Molecular Cloning, A Laboratory Manual, third edition).
In a next step according to the invention an amplification reaction is prepared. The contents of an amplification reaction are known by one skilled in the art and include appropriate substrates (such as dNTPs), enzymes (e.g. a DNA polymerase) and buffer components required for an amplification reaction. Generally amplification reactions require at least two amplification primers, often denoted ‘forward’ and ‘reverse’ primers (primer oligonucleotides) that are capable of annealing specifically to a part of the polynucleotide sequence to be amplified under conditions encountered in the primer annealing step of each cycle of an amplification reaction. In certain embodiments the forward and reverse primers may be identical. Thus the primer oligonucleotides must include an ‘adaptor-target specific portion’, being a sequence of nucleotides capable of annealing to a part of, that is, a primer-binding sequence, in the polynucleotide molecule to be amplified (or the complement thereof if the template is viewed as a single strand) during the annealing step.
Depending on the embodiment of the invention, the amplification primers may be universal for all samples, or one of the forward or reverse primers may carry the tag sequence that codes for the sample source. The amplification primers may hybridise across the tag region of the ligated adaptor, in which case unique primers will be needed for each sample nucleic acid. The amplification reaction may be performed with more than two amplification primers. In order to prevent the amplification of ligated adapter-adapter dimers, the amplification primers can be modified to contain nucleotides that hybridise across the whole of the ligated adapter and into the ligated template (or the dNTP's attached to the 3′ end thereof). This first amplification primer can be modified and treated to help prevent exonuclease digestion of the strands, and thus it may be advantageous to have a first amplification primer that is universal and can amplify all samples rather than modifying and treating each of the tagged primers separately. The tagged primer can be introduced as a sample specific third primer in the amplification reaction, but does not need to be specially modified and treated to reduce exonuclease digestion. The nested PCR approach is shown in
In the context of the present invention, the term ‘polynucleotide molecule to be amplified’ refers to the original or starting adaptor-target-adaptor sequence added to the amplification reaction. The ‘adaptor-target specific portion’ in the forward and reverse amplification primers refers to a sequence capable of annealing to the original or initial adaptor-target-adaptor present at the start of the amplification reaction and reference to the length of the ‘adaptor-target specific portion’ relates to the length of the sequence in the primer which anneals to the starting adaptor-target. It will be appreciated that if the primers contain any nucleotide sequence which does not anneal to the starting adaptor-target in the first amplification cycle then this sequence may be copied into the amplification products (assuming the primer does not contain a moiety which prevents read-through of the polymerase). Hence the amplified template strands produced in the first and subsequent cycles of amplification may be longer than the starting adaptor-target strands.
Since the mis-matched adapters can be different lengths, the length of adapter sequence added to the 3′ and 5′ ends of each strand may be different. The amplification primers may also be of different lengths to each other, and may hybridise to different lengths of the adapter, and therefore the length added to the ends of each strand can be controlled. In the case of nested PCR, the three or more amplification primers can be designed to be longer than the primer used to amplify the previous amplicon, so the length of the added nucleotides is fully controllable and may be hundreds of base pairs if desired. In the example shown in
The forward and reverse primers may be of sufficient length to hybridise to the whole of the adaptor sequence and at least one base of the target sequence (or the nucleotide DNTP added as a 3′-overhang on the target strands). The forward and reverse primers may also contain a region that extends beyond the adaptor construct, and therefore the amplification primers may be at least 20-100 bases in length. The forward and reverse primers may be of significantly different lengths; for example one may be 20-40 bases, whereas the other one may be 40-100 bases in length. The nucleotide sequences of the adaptor-target specific portions of the forward and reverse primers are selected to achieve specific hybridisation to the adaptor-target sequences to be amplified under the conditions of the annealing steps of the amplification reaction, whilst minimising non-specific hybridisation to any other target sequences present.
Skilled readers will appreciate that it is not strictly required for the adaptor-target specific portion to be 100% complementary, a satisfactory level of specific annealing can be achieved with less than perfectly complementary sequences. In particular, one or two mis-matches in the adaptor-target specific portion can usually be tolerated without adversely affecting specificity for the template. Therefore the term ‘adaptor-target specific portion’ should not be interpreted as requiring 100% complementarity with the adaptor-target. However, the requirement that the primers do not anneal non-specifically to regions of the adaptor-target other than their respective primer-binding sequences must be fulfilled.
Amplification primers are generally single stranded polynucleotide structures. They may also contain a mixture of natural and non-natural bases and also natural and non-natural backbone linkages, provided that any non-natural modifications do not preclude function as a primer—that being defined as the ability to anneal to a template polynucleotide strand during conditions of the amplification reaction and to act as an initiation point for synthesis of a new polynucleotide strand complementary to the template strand.
Primers may additionally comprise non-nucleotide chemical modifications, for example phosphorothioates to increase exonuclease resistance, again provided such that modifications do not prevent primer function. Modifications may, for example, facilitate attachment of the primer to a solid support, for example a biotin moiety. Certain modifications may themselves improve the function of the molecule as a primer, or may provide some other useful functionality, such as providing a site for cleavage to enable the primer (or an extended polynucleotide strand derived therefrom) to be cleaved from a solid support.
In an embodiment wherein tags are attached to the adaptors, the amplification can be carried out on either the pooled or unpooled samples. In an embodiment wherein universal adaptors are used, tags must be part of the amplification primers, and therefore, each sample must be amplified independently prior to pooling. The pooled nucleic acid samples can then be processed for sequencing
Preparation of Immobilised Samples for Sequencing
The pooled sample can then be immobilised in preparation for sequencing. Sequencing can be performed as an array of single molecules, or can be amplified prior to sequencing. The amplification can be carried out using one or more immobilised primers. The immobilised primer(s) can be a lawn on a planar surface, or on a pool of beads. The pool of beads can be isolated into an emulsion with a single bead in each ‘compartment’ of the emulsion. At a concentration of only one template per ‘compartment’, only a single template is amplified on each bead.
The term ‘solid-phase amplification’ as used herein refers to any nucleic acid amplification reaction carried out on or in association with a solid support such that all or a portion of the amplified products are immobilised on the solid support as they are formed. In particular, the term encompasses solid-phase polymerase chain reaction (solid-phase PCR) and solid phase isothermal amplification which are reactions analogous to standard solution phase amplification, except that one or both of the forward and reverse amplification primers is/are immobilised on the solid support. Solid phase PCR covers systems such as emulsions, wherein one primer is anchored to a bead and the other is in free solution, and colony formation in solid phase gel matrices wherein one primer is anchored to the surface, and one is in free solution.
Although the invention encompasses ‘solid-phase’ amplification methods in which only one amplification primer is immobilised (the other primer usually being present in free solution), it is preferred for the solid support to be provided with both the forward and the reverse primers immobilised. In practice, there will be a ‘plurality’ of identical forward primers and/or a ‘plurality’ of identical reverse primers immobilised on the solid support, since the amplification process requires an excess of primers to sustain amplification. References herein to forward and reverse primers are to be interpreted accordingly as encompassing a ‘plurality’ of such primers unless the context indicates otherwise.
As will be appreciated by the skilled reader, any given amplification reaction requires at least one type of forward primer and at least one type of reverse primer specific for the template to be amplified. However, in certain embodiments the forward and reverse primers may comprise template-specific portions of identical sequence, and may have entirely identical nucleotide sequence and structure (including any non-nucleotide modifications). In other words, it is possible to carry out solid-phase amplification using only one type of primer, and such single-primer methods are encompassed within the scope of the invention. Other embodiments may use forward and reverse primers which contain identical template-specific sequences but which differ in some other structural features. For example one type of primer may contain a non-nucleotide modification which is not present in the other.
In all embodiments of the invention, primers for solid-phase amplification are preferably immobilised by single point covalent attachment to the solid support at or near the 5′ end of the primer, leaving the template-specific portion of the primer free to anneal to its cognate template and the 3′ hydroxyl group free for primer extension. Any suitable covalent attachment means known in the art may be used for this purpose. The chosen attachment chemistry will depend on the nature of the solid support, and any derivatisation or functionalisation applied to it. The primer itself may include a moiety, which may be a non-nucleotide chemical modification, to facilitate attachment. In a particular embodiment, the primer may include a sulphur-containing nucleophile, such as phosphorothioate or thiophosphate, at the 5′ end. In the case of solid-supported polyacrylamide hydrogels (as described below), this nucleophile will bind to a bromoacetamide group present in the hydrogel. A more particular means of attaching primers and templates to a solid support is via 5′ phosphorothioate attachment to a hydrogel comprised of polymerised acrylamide and N-(5-bromoacetamidylpentyl) acrylamide (BRAPA), as described fully in WO05065814.
Certain embodiments of the invention may make use of solid supports comprised of an inert substrate or matrix (e.g. glass slides, polymer beads, etc) which has been “functionalised”, for example by application of a layer or coating of an intermediate material comprising reactive groups which permit covalent attachment to biomolecules, such as polynucleotides. Examples of such supports include, but are not limited to, polyacrylamide hydrogels supported on an inert substrate such as glass. In such embodiments, the biomolecules (e.g. polynucleotides) may be directly covalently attached to the intermediate material (e.g. the hydrogel), but the intermediate material may itself be non-covalently attached to the substrate or matrix (e.g. the glass substrate). The term “covalent attachment to a solid support” is to be interpreted accordingly as encompassing this type of arrangement.
The pooled samples may be amplified on beads wherein each bead contains a forward and reverse amplification primer. In a particular embodiment, the library of templates prepared according to the first, second or third aspects of the invention is used to prepare clustered arrays of nucleic acid colonies, analogous to those described in US20050100900, U.S. Pat. No. 7,115,400, WO 00/18957 and WO 98/44151, the contents of which are incorporated herein by reference in their entirety, by solid-phase amplification and more particularly solid phase isothermal amplification. The terms ‘cluster’ and ‘colony’ are used interchangeably herein to refer to a discrete site on a solid support comprised of a plurality of identical immobilised nucleic acid strands and a plurality of identical immobilised complementary nucleic acid strands. The term ‘clustered array’ refers to an array formed from such clusters or colonies. In this context the term ‘array’ is not to be understood as requiring an ordered arrangement of clusters.
The term solid phase, or surface, is used to mean either a planar array wherein primers are attached to a flat surface, for example, glass, silica or plastic microscope slides or similar flow cell devices; beads, wherein either one or two primers are attached to the beads and the beads are amplified; or an array of beads on a surface after the beads have been amplified.
Clustered arrays can be prepared using either a process of thermocycling, as described in WO9844151, or a process whereby the temperature is maintained as a constant, and the cycles of extension and denaturing are performed using changes of reagents. Such isothermal amplification methods are described in patent application numbers WO0246456 and US20080009420 (Isothermal methods for creating clonal single molecule arrays), which are incorporated herein by reference in their entirety. Due to the lower temperatures required in the isothermal process, this is particularly preferred.
Use in Sequencing/Methods of Sequencing
The invention also encompasses methods of sequencing amplified nucleic acids generated by solid-phase amplification. Thus, the invention provides a method of nucleic acid sequencing comprising amplifying a pool of nucleic acid templates using solid-phase amplification as described above and carrying out a nucleic acid sequencing reaction to determine the sequence of the whole or a part of at least one amplified nucleic acid strand produced in the solid-phase amplification reaction, as well as the sequence of the tag that codes for the identity of the sample.
Sequencing can be carried out using any suitable sequencing technique, wherein nucleotides are added successively to a free 3′ hydroxyl group, resulting in synthesis of a polynucleotide chain in the 5′ to 3′ direction. The nature of the nucleotide added is preferably determined after each nucleotide addition. Sequencing techniques using sequencing by ligation, wherein not every contiguous base is sequenced, and techniques such as massively parallel signature sequencing (MPSS) where bases are removed from, rather than added to the strands on the surface are also within the scope of the invention, as are techniques using detection of pyrophosphate release (pyrosequencing). Such pyrosequencing based techniques are particularly applicable to sequencing arrays of beads where the beads have been amplified in an emulsion such that a single template from the library molecule is amplified on each bead.
The initiation point for the sequencing reaction may be provided by annealing of a sequencing primer to a product of the solid-phase amplification reaction. In this connection, one or both of the adaptors added during formation of the template library may include a nucleotide sequence which permits annealing of a sequencing primer to amplified products derived by whole genome or solid-phase amplification of the template library.
Depending on the embodiment of the invention, the tag sequence and fragment sequence may be determined in a single read from a single sequencing primer, or in multiple reads from two sequencing primers. In the case of two reads from two sequencing primers, the ‘tag read’ and the ‘fragment read’ can be performed in either order, with a suitable denaturing step to remove the annealed primer after the first sequencing read is completed. Suitable denaturing steps may include formamide, hydroxide or heat as described elsewhere.
The products of solid-phase amplification reactions wherein both forward and reverse amplification primers are covalently immobilised on the solid surface are so-called ‘bridged’ structures formed by annealing of pairs of immobilised polynucleotide strands and immobilised complementary strands, both strands being attached to the solid support at the 5′ end. Arrays comprised of such bridged structures provide inefficient templates for nucleic acid sequencing, since hybridisation of a conventional sequencing primer to one of the immobilised strands is not favoured compared to annealing of this strand to its immobilised complementary strand under standard conditions for hybridisation.
In order to provide more suitable templates for nucleic acid sequencing, it is preferred to remove substantially all or remove or displace at least a portion of one of the immobilised strands in the ‘bridged’ structure in order to generate a template which is at least partially single-stranded. The portion of the template which is single-stranded will thus be available for hybridisation to a sequencing primer. The process of removing all or a portion of one immobilised strand in a ‘bridged’ double-stranded nucleic acid structure may be referred to herein as ‘linearisation’, and is described in further detail in WO07010251, the contents of which are incorporated herein by reference in their entirety.
Bridged template structures may be linearised by cleavage of one or both strands with a restriction endonuclease or by cleavage of one strand with a nicking endonuclease. Other methods of cleavage can be used as an alternative to restriction enzymes or nicking enzymes, including inter alia chemical cleavage (e.g. cleavage of a diol linkage with periodate), cleavage of abasic sites by cleavage with endonuclease (for example ‘USER’, as supplied by NEB, part number M5505S), or by exposure to heat or alkali, cleavage of ribonucleotides incorporated into amplification products otherwise comprised of deoxyribonucleotides, photochemical cleavage or cleavage of a peptide linker.
It will be appreciated that a linearization step may not be essential if the solid-phase amplification reaction is performed with only one primer covalently immobilised and the other in free solution.
Following the cleavage step, regardless of the method used for cleavage, the product of the cleavage reaction may be subjected to denaturing conditions in order to remove the portion(s) of the cleaved strand(s) that are not attached to the solid support. Suitable denaturing conditions, for example sodium hydroxide solution, formamide solution or heat, will be apparent to the skilled reader with reference to standard molecular biology protocols (Sambrook et al., 2001, Molecular Cloning, A Laboratory Manual, 3rd Ed, Cold Spring Harbor Laboratory Press, Cold Spring Harbor Laboratory Press, NY; Current Protocols, eds Ausubel et al.). Denaturation results in the production of a sequencing template which is partially or substantially single-stranded. A sequencing reaction may then be initiated by hybridisation of a sequencing primer to the single-stranded portion of the template.
Thus, the invention encompasses methods wherein the nucleic acid sequencing reaction comprises hybridising a sequencing primer to a single-stranded region of a linearised amplification product, sequentially incorporating one or more nucleotides into a polynucleotide strand complementary to the region of amplified template strand to be sequenced, identifying the base present in one or more of the incorporated nucleotide(s) and thereby determining the sequence of a region of the template strand.
One preferred sequencing method which can be used in accordance with the invention relies on the use of modified nucleotides having removable 3′ blocks, for example as described in WO04018497 and U.S. Pat. No. 7,057,026, the contents of which are incorporated herein by reference in their entirety. Once the modified nucleotide has been incorporated into the growing polynucleotide chain complementary to the region of the template being sequenced there is no free 3′-OH group available to direct further sequence extension and therefore the polymerase can not add further nucleotides. Once the nature of the base incorporated into the growing chain has been determined, the 3′ block may be removed to allow addition of the next successive nucleotide. By ordering the products derived using these modified nucleotides, it is possible to deduce the DNA sequence of the DNA template. Such reactions can be done in a single experiment if each of the modified nucleotides has a different label attached thereto, known to correspond to the particular base, to facilitate discrimination between the bases added during each incorporation step. Alternatively, a separate reaction may be carried out containing each of the modified nucleotides separately.
The modified nucleotides may carry a label to facilitate their detection. A fluorescent label, for example, may be used for detection of modified nucleotides. Each nucleotide type may thus carry a different fluorescent label, for example, as described in U.S. Provisional Application No. 60/801,270 (Novel dyes and the use of their labelled conjugates), published as WO07135368, the contents of which are incorporated herein by reference in their entirety. The detectable label need not, however, be a fluorescent label. Any label can be used which allows the detection of an incorporated nucleotide.
One method for detecting fluorescently labelled nucleotides comprises using laser light of a wavelength specific for the labelled nucleotides, or the use of other suitable sources of illumination. The fluorescence from the label on the nucleotide may be detected by a CCD camera or other suitable detection means. Suitable instrumentation for recording images of clustered arrays is described in U.S. Provisional Application No. 60/788,248 (Systems and devices for sequence by synthesis analysis), published as WO07123744, the contents of which are incorporated herein by reference in their entirety.
The invention is not intended to be limited to use of the sequencing method outlined above, as essentially any sequencing methodology which relies on successive incorporation of nucleotides into a polynucleotide chain can be used. Suitable alternative techniques include, for example, Pyrosequencing™, FISSEQ (fluorescent in situ sequencing), MPSS and sequencing by ligation-based methods, for example as described is U.S. Pat. No. 6,306,597.
The nucleic acid sample may be further analysed to obtain a second read from the opposite end of the fragment. Methodology for sequencing both ends of a cluster are described in co-pending applications WO07010252 and PCTGB2007/003798, the contents of which are incorporated by reference herein in their entirety. In one example, the series of steps may be performed as follows; generate clusters, linearise, hybridise first sequencing primer and obtain first sequencing read. The first sequencing primer can be removed, a second primer hybridised and the tag sequenced. The nucleic acid strand may then be ‘inverted’ on the surface by synthesising a complementary copy from the remaining immobilised primers used in cluster amplification. This process of strand resynthesis regenerates the double stranded cluster. The original template strand can be removed, to linearise the resynthesised strand that can then be annealed to a sequencing primer and sequenced in a third sequencing run.
In the cases where strand resynthesis is employed, both strands must be immobilised to the surface in a way that allows subsequent release of a portion of the immobilised strand. This can be achieved through a number of mechanisms as described in WO07010251, the contents of which are incorporated herein by reference in their entirety. For example, one primer can contain a uracil nucleotide, which means that the strand can be cleaved at the uracil base using the enzymes uracil glycosylase (UDG) which removes the nucleoside base, and endonuclease VIII that excises the abasic nucleotide. This enzyme combination is available as USER™ from New England Biolabs (NEB part number M5505). The second primer may comprise an 8-oxoguanine nucleotide, which is then cleavable by the enzyme FPG (NEB part number M0240). This design of primers provides complete control of which primer is cleaved at which point in the process, and also where in the cluster the cleavage occurs. The primers may also be chemically modified, for example with a disulfide or diol modification that allows chemical cleavage at specific locations.
The invention also relates to kits for use in preparing libraries of tagged polynucleotides using the method of the first, second or third aspects of the invention.
Embodiments of the kit comprise at least a supply of a mismatched adaptor as defined herein, plus a supply of at least one amplification primer which is capable of annealing to the mismatched adaptor and priming synthesis of an extension product, which extension product would include any target sequence ligated to the adaptor when the adaptor is in use.
Particular features of the ‘mismatch’ adaptors for inclusion in the kit are as described elsewhere herein in relation to other aspects of the invention. The structure and properties of amplification primers are well known to those skilled in the art. Suitable primers of appropriate nucleotide sequence for use with the adaptors included in the kit can be readily prepared using standard automated nucleic acid synthesis equipment and reagents in routine use in the art. The kit may include a supply of one single type of primer or separate supplies (or even a mixture) of two different primers, for example a pair of amplification primers suitable for PCR or isothermal amplification of templates modified with the mismatched adaptor in solution phase and/or on a suitable solid support (i.e. solid-phase amplification). The kit may comprise a mismatch double stranded adapter for ligation to a sample of interest, plus at least two different amplification primers that carry a different tag sequence, where the tag sequence does not hybridise to the adapter. This kit can be used to amplify at least two different samples where each sample is amplified using a single tagged primer, and then pooled after the individual amplification reactions.
In one embodiment the kit may include supplies of different primer-pairs for use in solution phase and solid phase PCR and more particularly isothermal amplification. In this context the ‘different’ primer-pairs may be of substantially identical nucleotide sequence but differ with respect to some other feature or modification, such as for example surface-capture moieties, etc. In other embodiments the kit may include a supply of primers for use in an initial primer extension reaction and a different primer-pair (or pairs) for solution and/or solid phase amplification.
Adaptors and/or primers may be supplied in the kits ready for use, or more preferably as concentrates requiring dilution before use, or even in a lyophilised or dried form requiring reconstitution prior to use. If required, the kits may further include a supply of a suitable diluent for dilution or reconstitution of the primers. Optionally, the kits may further comprise supplies of reagents, buffers, enzymes, dNTPs, etc., for use in carrying out PCR or isothermal amplification. Suitable (but non-limiting) examples of such reagents are as described in the Materials and Methods sections of the accompanying Examples. Further components which may optionally be supplied in the kit include ‘universal’ sequencing primers suitable for sequencing templates prepared using the mismatched adaptors and primers.
The invention will be further understood with reference to the following non-limiting experimental examples:
The following are examples of general techniques which may be applied in carrying out the method of the invention.
The following experimental details describe the complete exposition of one embodiment of the invention as described above.
Two libraries were made, one using purified human BAC DNA (140 k human chromosome 6 insert cloned into a pTARBAC vector) and the other purified PhiX174 RF1 DNA (NEB, N3021L). Each library was prepared separately. The DNA was first prepared for ligation to forked adaptors by: fragmentation of the DNA by nebulisation, end repair of the DNA ends to render them blunt-ended and phosphorylated, then the addition of a single ‘A’ nucleotide onto the 3′ ends of the DNA fragments. The ligation reaction was performed with the prepared fragmented DNA and adaptors pre-formed by annealing ‘Oligo A’ and ‘Oligo B’ (sequences given below). The same adaptors were used for each library. The product of the reaction was isolated/purified from unligated adaptor by gel electrophoresis. Finally, the product of the ligation reaction was subjected to cycles of PCR to selectively amplify ligated product that contained genomic DNA with adaptor at both ends of the fragments. During the PCR a unique tag was added to each library using a unique PCR primer, so that the BAC library was indexed with the unique sequence tag ‘ATC’ and the PhiX library was indexed with the unique sequence tag ‘CGA’. See
Materials and Methods
Step 1) Nebulization
Mixed 5 μl (5 μg) of PhiX174 DNA with 45 μl of TE and 700 μl 1 of nebulization buffer. Mixed 10 Al (5 μg) of BAC DNA with 40 μl of TE and 700 μl of nebulization buffer. Chilled DNA solutions were each fragmented in a nebulizer on ice for 6 minutes under 32 pounds per square inch (psi) of pressure. The recovered volumes were each purified with a Qiagen PCR purification kit column and eluted in 30 μl of EB.
Step 2) End-Repair
End repair mix was assembled as follows:
Nebulized DNA 30 μl Water 45 μl T4 DNA ligase buffer with 10 mM ATP 10 μl dNTPs 4 μl T4 DNA pol 5 μl Klenow DNA pol 1 ul T4 PNK 5 ul 100 μl total
The reaction was incubated for 30 minutes at room temperature. The DNA was purified on a Qiagen column, eluting in 30 μl EB.
Step 3) A-Tailing Reaction
The following reaction mix was assembled:
End repaired DNA 30 μl Water 2 ul NEB buffer 2 5 μl dATP 10 μl Klenow fragment (3′ to 5′ exo minus) 3 μl 50 μl total
The reaction was incubated for 30 minutes at 37° C., then the DNA purified on a Qiagen MinElute column, eluting in 10 μl EB.
Step 4) Annealed Adaptors
The oligos were mixed together to a final concentration of 15 uM each, in 10 mM Tris/10 mM NaCl pH 7.0. The adaptor strands were annealed in a PCR machine programmed as follows: Ramp at 0.5° C./sec to 97.5° C.; Hold at 97.5° C. for 150 sec; then a step of 97.5° C. for 2 sec with a temperature drop of 0.1° C./cycle for 775 cycles.
In order to ensure that a sequencing primer is attached to both ends of the adapter for the paired end method, the sequence of oligonucleotide B was changed to: 5′Phosphate-GATCGGAAGAGCACACGTCT 3′ (SEQ ID NO. 3)
Step 5) Ligation
Reaction mix was assembled as follows:
A-tailed genomic DNA 10 μl Quick ligase buffer 25 μl Annealed adaptor 10 μl Quick Ligase 5 μl 50 μl total
The reaction was incubated for 15 minutes at room temperature, then the DNA purified on a Qiagen column, eluting in 30 μl EB.
Step 6) Gel Purification
The entire sample from the purified ligation reaction was loaded into one lane of a 2% agarose gel containing ethidium bromide and run at 120V for 60 minutes. The gel was then viewed on a ‘White-light’ box and fragments from 120 bp to 170 bp excised and purified with a gel extraction column, eluting in 30 μl elution buffer (EB).
Step 7) Exonuclease I Treatment of PCR Primers
DNA Primers with a phosphorothioate at the n−1 position (5×85 μl of each Primer (approx 25 μM)) were aliquoted into Eppendorf tubes. 10 μl of 10× Exonuclease I Reaction Buffer and 5 μl of Exonuclease I was added to each tube. Each Eppendorf tube was placed in a rack and stored in an oven set at 37° C. for 16 hours. After 16 hr, the tubes were placed on a hotblock set at 80° C. for 2 minutes. Subsequently, the solutions from the Eppendorfs were passed through P6 Bio-Rad columns and spun in a centrifuge at 2000 rpm for 2 minutes. An extra 20 μl of H20 was added to the columns and the columns respun. The filtered solutions were placed into a SpeedVac® and evaporated until each was at 20 μl, and the fractions combined. The pooled fractions were injected into a reverse phase HPLC system, and the main peak was collected. The collected fractions were evaporated to dryness in a SpeedVac®, 50 μl of water was added and the fraction was subjected again to evaporation to dryness. The resulting pellets were dissolved in 50 μl of water, pooled and a UV measurement taken to determine the concentration of the oligonucleotide.
Step 8) PCR
The PCR reaction was prepared as follows:
Gel purified BAC DNA
Universal PCR primer
Indexing PCR primer 1
Gel purified PhiX174 DNA
Universal PCR primer
Indexing PCR primer 2
Thermocycling was carried out in a PCR machine under the following conditions:
PCR products were purified on a Qiagen column, eluting in 30 μl EB. The resulting DNA libraries were ready for mixing and amplification on a surface amplification platform.
In the case of paired end runs, the human and Phi-X sample were split into 6 portions, and each portion was amplified with the two universal primers plus one of the 12 primers shown below.
Universal LPX primer
(SEQ ID NO. 7)
5′ GTGACTGGAGTTCAGACGTGTGCTCTTCCGATCxT 3′
(SEQ ID NO. 8)
Tag1 primer (CGTGAT)
(SEQ ID NO. 9)
5′ CAAGCAGAAGACGGCATACGAGATCGTGATGTGACTGGAGTTC 3′
Tag2 primer (ACATCG)
(SEQ ID NO. 10)
5′ CAAGCAGAAGACGGCATACGAGATACATCGGTGACTGGAGTTC 3′
Tag3 primer (GCCTAA)
(SEQ ID NO. 11)
5′ CAAGCAGAAGACGGCATACGAGATGCCTAAGTGACTGGAGTTC 3′
Tag4 primer (TGGTCA)
(SEQ ID NO. 12)
5′ CAAGCAGAAGACGGCATACGAGATTGGTCAGTGACTGGAGTTC 3′
Tags primer (CACTGT)
(SEQ ID NO. 13)
5′ CAAGCAGAAGACGGCATACGAGATCACTGTGTGACTGGAGTTC 3′
Tag6 primer (ATTGGC)
(SEQ ID NO. 14)
5′ CAAGCAGAAGACGGCATACGAGATATTGGCGTGACTGGAGTTC 3′
Tag7 primer (GATCTG)
(SEQ ID NO. 15)
5′ CAAGCAGAAGACGGCATACGAGATGATCTGGTGACTGGAGTTC 3′
TagB primer (TCAAGT)
(SEQ ID NO. 16)
5′ CAAGCAGAAGACGGCATACGAGATTCAAGTGTGACTGGAGTTC 3′
Tag9 primer (GTGATC)
(SEQ ID NO. 17)
5′ CAAGCAGAAGACGGCATACGAGATCTGATCGTGACTGGAGTTC 3′
Tag10 primer (AAGCTA)
(SEQ ID NO. 18)
5′ CAAGCAGAAGACGGCATACGAGATAAGCTAGTGACTGGAGTTC 3′
Tag11 primer (GTAGCC)
(SEQ ID NO. 19)
5′ CAAGCAGAAGACGGCATACGAGATGTAGCCGTGACTGGAGTTC 3′
Tag12 primer (TACAAG)
(SEQ ID NO. 20)
5′ CAAGCAGAAGACGGCATACGAGATTACAAGGTGACTGGAGTTC 3′
The two universal primers contain a phosphorothioate group (x) and were exonucleases treated and purified prior to amplification. The amplification conditions were as described above, and the 6 tagged human samples, and 6 tagged Phi-X sample were pooled together for sequencing on clusters.
Validation of Libraries by Conventional Sanger Sequencing
Four (4) μl of the libraries were cloned into a plasmid vector (Zero Blunt TOPO PCR cloning kit, Invitrogen #K2800-20) and plated out on agar, according to the manufacturer's instructions. Colonies were picked, mini-prepped and the cloned fragments sequenced by conventional Sanger sequencing.
These results confirm that the library preparation method produces 2 libraries of ‘sequenceable’ DNA templates. Each library contained a plurality of genomic inserts, each of which was flanked by the two adaptors
required for cluster formation and SBS sequencing. The insert DNA from each of the libraries aligned to the correct reference, either BAC or PhiX, with a small amount of E. coli contamination in each library. The correct TAG (
The solid supports used are typically 8-channel glass chips such as those provided by Silex Microsystems (Sweden). However, the experimental conditions and procedures are readily applicable to other solid supports.
Chips were washed as follows: neat Decon for 30 minutes, milliQ H2O for 30 minutes, NaOH 1N for 15 minutes, milliQ H2O for 30 minutes, HCl 0.1N for 15 minutes, milliQ H2O for 30 minutes.
Polymer Solution Preparation:
For 10 ml of 2% polymerisation mix.
The 10 ml solution of acrylamide was first degassed with argon for 15 minutes. The solutions of BRAPA, TEMED and potassium persulfate were successively added to the acrylamide solution. The mixture was then quickly vortexed and immediately used. Polymerization was then carried out for 1 h 30 minutes at RT. Afterwards the channels were washed with milliQ H2O for 30 minutes and filled with 0.1 M potassium phosphate buffer for storage until required.
N-Boc-1,5-diaminopentane toluene sulfonic acid was obtained from Novabiochem. The bromoacetyl chloride and acryloyl chloride were obtained from Fluka. All other reagents were Aldrich products.
To a stirred suspension of N-Boc-1,5-diaminopentane toluene sulfonic acid (5.2 g, 13.88 mmol) and triethylamine (4.83 ml, 2.5 eq) in THF (120 ml) at 0° C. was added acryloyl chloride (1.13 ml, 1 eq) through a pressure equalized dropping funnel over a one hour period. The reaction mixture was then stirred at room temperature and the progress of the reaction checked by TLC (petroleum ether:ethyl acetate 1:1). After two hours, the salts formed during the reaction were filtered off and the filtrate evaporated to dryness. The residue was purified by flash chromatography (neat petroleum ether followed by a gradient of ethyl acetate up to 60%) to yield 2.56 g (9.98 mmol, 71%) of product 2 as a beige solid. 1H NMR (400 MHz, d6-DMSO): 1.20-1.22 (m, 2H, CH2), 1.29-1.43 (m, 13H, tBu, 2×CH2), 2.86 (q, 2H, J=6.8 Hz and 12.9 Hz, CH2), 3.07 (q, 2H, J=6.8 Hz and 12.9 Hz, CH2), 5.53 (dd, 1H, J=2.3 Hz and 10.1 Hz, CH), 6.05 (dd, 1H, J=2.3 Hz and 17.2 Hz, CH), 6.20 (dd, 1H, J=10.1 Hz and 17.2 Hz, CH), 6.77 (t, 1H, J=5.3 Hz, NH), 8.04 (bs, 1H, NH). Mass (electrospray+) calculated for C13H24N2O3 256, found 279 (256+Na+)
Product 2 (2.56 g, 10 mmol) was dissolved in trifluoroacetic acid:dichloromethane (1:9, 100 ml) and stirred at room temperature. The progress of the reaction was monitored by TLC (dichloromethane:methanol 9:1). On completion, the reaction mixture was evaporated to dryness, the residue co-evaporated three times with toluene and then purified by flash chromatography (neat dichloromethane followed by a gradient of methanol up to 20%). Product 3 was obtained as a white powder (2.43 g, 9 mmol, 90%). 1H NMR (400 MHz, D2O): 1.29-1.40 (m, 2H, CH2), 1.52 (quint., 2H, J=7.1 Hz, CH2), 1.61 (quint., 2H, J=7.7 Hz, CH2), 2.92 (t, 2H, J=7.6 Hz, CH2), 3.21 (t, 2H, J=6.8 Hz, CH2), 5.68 (dd, 1H, J=1.5 Hz and 10.1 Hz, CH), 6.10 (dd, 1H, J=1.5 Hz and 17.2 Hz, CH), 6.20 (dd, 1H, J=10.1 Hz and 17.2 Hz, CH). Mass (electrospray+) calculated for C8H16N2O 156, found 179 (156+Na+).
To a suspension of product 3 (6.12 g, 22.64 mmol) and triethylamine (6.94 ml, 2.2 eq) in THF (120 ml) was added bromoacetyl chloride (2.07 ml, 1.1 eq), through a pressure equalized dropping funnel, over a one hour period and at −60° C. (cardice and isopropanol bath in a Dewar). The reaction mixture was then stirred at room temperature overnight and the completion of the reaction was checked by TLC (dichloromethane:methanol 9:1) the following day. The salts formed during the reaction were filtered off and the reaction mixture evaporated to dryness. The residue was purified by chromatography (neat dichloromethane followed by a gradient of methanol up to 5%). 3.2 g (11.55 mmol, 51%) of the product 1 (BRAPA) were obtained as a white powder. A further recrystallization performed in petroleum ether:ethyl acetate gave 3 g of the product 1. 1H NMR (400 MHz, d6-DMSO) δ 1.21-1.30 (m, 2H, CH2), 1.34-1.48 (m, 4H, 2×CH2), 3.02-3.12 (m, 4H, 2×CH2), 3.81 (s, 2H, CH2), 5.56 (d, 1H, J=9.85 Hz, CH), 6.07 (d, 1H, J=16.9 Hz, CH), 6.20 (dd, 1H, J=10.1 Hz and 16.9 Hz, CH), 8.07 (bs, 1H, NH), 8.27 (bs, 1H, NH). Mass (electrospray+) calculated for C10H17BrN2O2 276 or 278, found 279 (278+H+), 299 (276+Na+).
An SFA coated chip is placed onto a modified MJ-Research thermocycler and attached to a peristaltic pump. Grafting mix consisting of 0.5 μM of a forward primer and 0.5 μM of a reverse primer in 10 mM phosphate buffer (pH 7.0) is pumped into the channels of the chip at a flow rate of 60 μl/minutes for 75 s at 20° C. The thermocycler is then heated to 51.6° C., and the chip is incubated at this temperature for 1 hour. During this time, the grafting mix undergoes 18 cycles of pumping: grafting mix is pumped in at 15 μl/minutes for 20 s, then the solution is pumped back and forth (5 s forward at 15 μl/minutes, then 5 s backward at 15 μl/minutes) for 180 s. After 18 cycles of pumping, the chip is washed by pumping in 5×SSC/5 mM EDTA at 15 μl/minutes for 300 s at 51.6° C. The thermocycler is then cooled to 20° C.
The primers are typically 5′-phosphorothioate oligonucleotides incorporating any specific sequences or modifications required for cleavage. Their sequences and suppliers vary according to the experiment for which they are to be used, and in this case were complementary to the 5′-ends of the template duplex. The DNA sequence used in this process was the pool of the two libraries, which have ends complementary to the grafted primers. The library mix was denatured using sodium hydroxide treatment followed by snap dilution as described.
For some of the experiments detailed, the amplified clusters contained a diol linkage in one of the grafted primers. Diol linkages can be introduced by including a suitable linkage into one of the primers used for solid-phase amplification. Synthesis of the diol phosphoramidite is described in Example 4 below. Products containing such diol linkages can be cleaved using periodate and propanolamine as described, and the resulting single stranded polynucleotides hybridised as described.
The grafted primers contain a sequence of T bases at the 5′-end to act as a spacer group to aid linearisation and hybridization. The sequences of the two primers grafted to the chip are as follows:
(SEQ ID NO. 55)
(SEQ ID NO. 56)
1,6-Hexanediol (Sigma Aldrich 99%) (14.6 g, 124 mmol), N,N-diisopropylethylamine (Hünig's base; Sigma Aldrich; redistilled) (21.6 mL, 124 mmol) is dissolved in anhydrous DCM/DMF (250/50 mL) under N2. The solution is cooled to 0° C. and the first portion of 4,4′-dimethoxytrityl chloride (DMTr-Cl; Sigma-Aldrich 95%) (10.5 g, 31 mmol) is added. The reaction mixture is then warmed to room temperature. After stirring for 1 h, the reaction mixture is cooled to 0° C. again and the second portion of DMTr-Cl (10.5 g, 31 mmol) is added and then allowed to stir at room temperature for another 2 hours. TLC (EtOAc: petroleum ether 4:6) analysis indicates ca. 95% consumption of starting material derivative (DMTr-OH). The reaction is concentrated under reduced pressure and Aq. NaHCO3 (sat.) solution (500 mL) is poured into the residue. The resulting mixture is extracted with petroleum ether/EtOAc (2:1) (3×1000 mL). The combined organic layers are dried over MgSO4, and concentrated under vacuum. The residue is co-evaporated with xylene (2×100 mL) to remove DMF. The reaction mixture, is pre-absorbed on silica gel and subjected to flash chromatography using solvents containing 1% Et3N petroleum ether to petroleum ether/EtOAc (7:3) as eluent. The yield of pale yellow oil is 16.58 g, 64%, with a further 7.8 g (17%) of the bis-tritylated by-product.
TLC: Rf: 0.35 (diol-1); Rf: 0.7 (bis-tritylated by-product) (petroleum ether/EtOAc 6:4).
1H NMR (400 MHz, CDCl3): δ 1.32-1.44 (m, 4H, 2×CH2), 1.54-1.68 (m, 4H, 2×CH2), 3.06 (t, J=6.6 Hz, 2H, CH2O), 3.62-3.68 (m, 2H, CH2OH), 3.81 (s, 6H, 2× MeO), 6.83-6.85 (m, 4H, Ph), 7.24-7.35 (m, 7H, Ph), 7.45-7.47 (m, 2H, Ph).
To a solution of Diol-1 (16.6 g, 39.5 mmol) in anhydrous DCM (200 mL), tetrapropylammonium perruthenate (TPAP; Sigma Aldrich 97%) (277 mg, 0.79 mmol) is added under N2 atmosphere. The solution is cooled to 0° C. and N-methylmopholine N-oxide (Sigma Aldrich 97%) (2.7 g, 23 mmol) is added. The reaction is warmed to room temperature. After 1 hour, the other three portions of N-methylmopholine N-oxide (3×2.0 g, 51.2 mmol) are added within a period of four hours. TLC (EtOAc: petroleum ether 4:6) indicates the reaction goes to completion. The reaction is quenched with aq. NaHCO3 (sat.) (1000 mL) and extracted to CH2Cl2 (4×1000 mL). The combined organic layers are dried over MgSO4. The solution is concentrated under reduced pressure. Diol-3, 9.9 g, 60%, is isolated by flash chromatography using solvents containing 1% Et3N from petroleum ether to petroleum ether/EtOAc (6:4) as eluent, as a pale yellow oil.
TLC: Rf: 0.7 (petroleum ether/EtOAc 6:4).
1H NMR (400 MHz, CDCl3): δ 1.30-1.37 (m, 2H, CH2), 1.48-1.57 (m, 4H, 2×CH2), 2.34 (td, J=1.7 and 7.4 Hz, 2H, CH2CHO), 2.97 (s, 2H, CH2O), 3.72 (s, 6H, 2× MeO), 6.73-6.76 (m, 4H, Ph), 7.10-7.26 (m, 7H, Ph), 7.34-7.36 (m, 2H, Ph), 9.67 (t, J=1.7, 1H, CHO).
A solution of triphenylphosphine (Sigma-Aldrich 99%, ReagentPlus™). (39.3 g, 150 mmol) and 4-bromobutyl acetate (Sigma-Aldrich)(26 mL, 180 mmol) in anhydrous toluene (300 mL) is heated under reflux for 36 hours under N2 in an oil-bath (140° C.). During the reflux, oil is precipitated out. The reaction mixture is cooled to room temperature. TLC (petroleum ether/EtOAc 7:3) analysis of the toluene solution showed that there is still triphenylphosphine (Rf: 0.8) left. The supernatant is decanted into another round-bottomed flask and concentrated down to the approximate volume of 30 mL. The solution is heated under reflux again for another 12 hours. The supernatant is decanted. The portions of oil are combined together, dissolved in water (500 mL) and extracted with EtOAc (2×500 mL). The combined organic layers are back-extracted with water (150 mL). Two lots of aqueous layers are combined, and evaporated under reduced pressure. The resulting residue is co-evaporated with acetonitrile (2×100 mL) to give 78.4 g, 95% yield of a pale yellow oil. NMR indicates that the product is pure, and is used for the next step reaction without further purification.
TLC: Rf: 0.0 (petroleum ether/EtOAc 7:3).
1H NMR (400 MHz, CDCl3): δ 1.63-1.73 (m, 2H, CH2) 1.94 (s, 3H, 2×CH3), 2.06-2.16 (m, 2H, CH2), 3.97-4.05 (m, 2H, CH2P), 4.11 (t, J=6.0, 2H, CH2O), 7.69-7.95 (m, 15H, Ph).
31P NMR (162 MHz, CDCl3): 25.9 ppm.
Mass spec details: LC-MS (Electrospray positive): (M+) 377.
Diol-2 (10.34 g, 22.7 mmol) is weighed into a round-bottomed flask and dissolved with DCM (20 mL). The solution is then evaporated under reduced pressure until it gives a white foam. The flask is then subjected to high vacuum for 24 h. To this flask, anhydrous THF (180 mL) is added under N2. The resulting suspension is cooled to −78° C. with an acetone-dry ice bath. With vigorous stirring, KOBut (3.3 g, 29.5 mmol) is added under N2. Slowly the colour of the suspension turns orange, and white solids are gradually precipitated out. To this suspension, a solution of diol-3 (dried at 60° C. under high vacuum for 1 h before the reaction), (9.5 g, 22.7 mmol) in THF (50 mL) is added drop wise over half an hour. Acetone-dry ice bath is then removed. The reaction mixture is slowly warmed to room temperature and stirred for another hour. The colour of the reaction mixture turns yellow after the addition of diol-3. The reaction mixture is concentrated down under reduced pressure. The resulting residue is partitioned between DCM (800 mL) and aq. NaCl (sat.) (800 mL). The aqueous layer is extracted with an additional DCM (2×800 mL). The organic extractions are combined, dried over MgSO4, filtered, and evaporated under reduced pressure to give yellow oil. The oil is dissolved in THF/MeOH (125/100 mL) and cooled to 0° C. To this solution, NaOH (1M in H2O, 25 mL) is added. After allowing the reaction to stir for 1 hour, TLC analysis indicates full consumption of starting material. The reaction mixture is neutralized with acetic acid (1.5 mL). The reaction mixture is concentrated down under reduced pressure. The resulting residue is partitioned between DCM (800 mL) and aq. NaHCO3 (sat.) (800 mL). The aqueous layer is extracted with additional DCM (2×800 mL). The organic extractions are combined, dried over MgSO4, filtered, and evaporated to give a pale yellow oil. Diol-4, 6.45 g, 60% is isolated by flash chromatography using solvents containing 1% Et3N from petroleum ether to petroleum ether/EtOAc (5:5) as eluent, as a light yellow oil.
TLC: Rf=0.45 (petroleum ether/EtOAc 6:4).
1H NMR (400 MHz, CDCl3) δ 1.24-1.32 (m, 4H, 2×CH2), 1.54-1.57 (m, 4H, 2×CH2), 1.93-1.96 (m, 2H, CH2) 2.02-2.07 (m, 2H, CH2), 2.96 (t, J=6.6 Hz, 2H, CH2O), 3.54-3.59 (m, 2H, CH2OH), 3.72 (s, 6H, 2× MeO), 5.29-5.32 (m, 2H, 2×=CH), 6.73-6.77 (m, 4H, Ph), 7.11-7.27 (m, 7H, Ph), 7.36-7.38 (m, 2H, Ph).
To a solution of Diol-4 (5.68 g, 12 mmol) and imidazole (Sigma Aldrich, 99%), (1.63 g, 24 mmol) in anhydrous DMF (100 mL), t-butyldiphenylsilyl chloride (Sigma Aldrich, 98%), (4.05 mL, 15.6 mmol) is added drop wise under N2 atmosphere at room temperature. The reaction is stirred for 1 hour. TLC (petroleum ether/EtOAc 8:2) indicates that the starting material is fully consumed. A saturated aq. NaHCO3 solution (500 mL) is added to quench the reaction. The resulting mixture is extracted with petroleum ether/EtOAc (2:1) (3×500 mL). The organic layers are combined, dried over MgSO4, filtered, and evaporated to give a yellow oil. Diol-5, 8.14 g, 95% is isolated by flash chromatography using solvents containing 1% Et3N from petroleum ether to petroleum ether/EtOAc (9:1) as eluent, as a colourless oil.
TLC: Rf=0.7 (petroleum ether:EtOAc 8:2).
1H NMR (400 MHz, CDCl3): δ 0.97 (s, 9H, 3× Me) 1.19-1.30 (m, 4H, 2×CH2), 1.48-1.55 (m, 4H, 2×CH2), 1.91-1.95 (m, 2H, CH2), 2.01-2.06 (m, 2H, CH2), 2.95 (t, J=6.6 Hz, 2H, CH2O), 3.58 (t, J=6.3 Hz, 2H, CH2O), 3.70 (s, 6H, 2× MeO), 5.24-5.27 (m, 2H, 2×=CH), 6.72-6.75 (m, 4H, Ph), 7.11-7.37 (m, 15H, Ph), 7.57-7.60 (m, 4H, Ph).
A mixture of diol-5 (9.27 g, 13 mmol), AD-mix-α (Sigma Aldrich), (18.2 g), methanesulfonamide (Sigma Aldrich, 97%), (1.23 g, 13 mmol), t-BuOH (65 mL) and water (65 mL) is stirred together vigorously at 55° C. for 14 h. The TLC analysis (petroleum ether:EtOAc 6:4) indicates ca. 95% consumption of the starting material. The reaction mixture is cooled to room temperature, treated with sodium sulfite (15.3 g, 12 mmol), then further stirred for 30 minutes. A saturated aq. NaHCO3 solution (500 mL) is added to the reaction. The resulting mixture is extracted with EtOAc (3×500 mL). The organic layers are combined, dried over MgSO4, filtered, and evaporated to give yellow oil. Diol-6, 7.96 g, 82%, is isolated by flash chromatography (silica gel, Fluka, 70-230 mesh) using solvents containing 1% Et3N from petroleum ether to petroleum ether/EtOAc (1:1) as elutant, as a white solid.
TLC: Rf=0.3 (petroleum ether:EtOAc 6:4).
1H NMR (400 MHz, CDCl3) δ 1.07 (s, 9 H, 3× Me), 1.41-1.7 (m, 12 H, 6×CH2), 1.94 (d, J=4.3 Hz, 1H, OH) 2.94-2.95 (m, 1H, OH), 3.06 (t, J=6.6 Hz, 2H, CH2O), 3.61-3.63 (m, 2 H, 2×CHOH), 3.73 (t, J=5.6 Hz, 2H, CH2O), 3.81 (s, 6H, 2× MeO), 5.24-5.27 (m, 2H, 2×=CH), 6.82-6.85 (m, 4H, Ph), 7.21-7.47 (m, 15 H, Ph), 7.57-7.60 (m, 4 H, Ph).
To a solution of diol-6 (7.96 g, 13 mmol) and DMAP (Sigma-Aldrich ReagentPlus™, 99%). (260 mg, 2.13 mmol) in a mixture of pyridine (15 mL) and DCM (30 mL), acetic anhydride (Fluka 99%), (2.5 mL, 26.68 mmol) is added at room temperature. TLC analysis (petroleum ether:EtOAc 6:4) indicates full consumption of the starting material after 1 h. The reaction is quenched by saturated aq. NaHCO3 solution (500 mL). After 5 minutes, the mixture is extracted with DCM (3×500 mL). The organic layers are combined, dried over MgSO4, filtered, and evaporated. The residue is co-evaporated with toluene (2×100 mL). The resulting yellow oil is subjected to a plug of silica gel (50 g, Fluka, 70-230 mesh) to remove DMAP using eluents containing 0.1% Et3N from petroleum ether to petroleum ether/EtOAc (7:3) (250 mL each). The combined fractions of product are concentrated to dryness. The resulting colourless oil is dissolved in THF (100 mL) and treated with TBAF (Sigma-Aldrich; 5% wt water), (1 M in THF, 15 mL) at 0° C. The reaction solution is slowly warmed to room temperature and stirred for 2 hours. TLC analysis (petroleum ether:EtOAc 6:4) indicates that desilylation is completed. The volatile solvent (THF) is evaporated under reduced pressure at low temperature. A saturated aq. NaHCO3 solution (500 mL) is added to the residue. The resulting mixture is extracted with EtOAc (3×500 mL). The organic layers are combined, dried over MgSO4, filtered, and evaporated to give yellow oil. Diol-7, 4.2 g, 66%, is isolated by flash chromatography using solvents containing 1% Et3N from petroleum ether to petroleum ether/EtOAc (1:1) as eluent, as a white solid.
TLC: Rf=0.45 (petroleum ether:EtOAc 1:1).
1H NMR (400 MHz, CDCl3) δ 1.29-1.33 (m, 4H, 2×CH2), 1.47-1.63 (m, 8H, 4×CH2), 1.99, 2.01 (2s, 6H, 2 MeC(O)), 3.00 (t, J=6.5 Hz, 2H, CH2O), 3.60-3.64 (m, 2 H, CH2O), 3.75 (s, 6H, 2× MeO), 4.92-4.97 (m, 2H, 2× CHOAc), 6.76-6.80 (m, 4H, Ph), 7.15-7.29 (m, 7 H, Ph), 7.38-7.40 (m, 2 H, Ph).
To a solution of diol-7 (2.08 g, 3.5 mmol) and diisopropylethylamine (Sigma Aldrich), (1.53 ml, 8.75 mmol) in DCM (17 mL), 2-cyanoethyl N,N-diisopropylchlorophosphor-amidite (1.0 g, 4.2 mmol) is added drop wise at room temperature under N2. After stirring for 1 hour, TLC analysis (petroleum ether:EtOAc 4:6) indicates the full consumption of the starting material. The solvent (THF) is concentrated under reduced pressure. The resulting residue is subjected to chromatography directly. Diol-8, 2.5 g, 90%, is isolated by flash chromatography using solvents containing 1% Et3N from petroleum ether to petroleum ether/EtOAc (1:1) as eluent, as a colourless syrup.
TLC: Rf=0.55 (petroleum ether:EtOAc 4:6).
1H NMR (400 MHz, CDCl3) δ 1.09, 1.10, 1.11, 1.12 (4 s, 12 H, N(CHMe2)2), 1.26-1.31 (m, 4H, 2×CH2), 1.45-1.56 (m, 8 H, 4×CH2), 1.95, 1.969, 1.971, 1.98 (4 s, 6H, 2 MeCO), 2.56 (t, J=6.5 Hz, 2H, CH2CN), 2.95 (t, J=6.5 Hz, 2H, CH2O), 3.49-3.55 (m, 4 H, CH2O), 3.72 (s, 6H, 2× MeO), 4.89-4.92 (m, 2H, 2× CHOAc), 6.74-6.76 (m, 4H, Ph), 7.13-7.25 (m, 7 H, Ph), 7.34-7.37 (m, 2 H, Ph).
31P NMR (162 MHz, CDCl3): 148.67, 148.69 ppm.
Step 1: Hybridisation and Amplification
The DNA sequence used in the amplification process is the mixture of the two libraries prepared in Example 1, which have ends complementary to the grafted primers. The duplex DNA (1 nM) is denatured using 0.1 M sodium hydroxide treatment followed by snap dilution to the desired 0.2-2 pM ‘working concentration’ in ‘hybridization buffer’ (5×SSC/0.1% Tween).
Surface amplification was carried out by isothermal amplification using an MJ Research thermocycler, coupled with an 8-way peristaltic pump Ismatec IPC ISM931 equipped with Ismatec tubing (orange/yellow, 0.51 mm ID). A schematic of the instrument is shown in
The single stranded template (denatured as indicated above) is hybridised to the grafted primers immediately prior to the amplification reaction, which thus begins with an initial primer extension step rather than template denaturation. The hybridization procedure begins with a heating step in a stringent buffer to ensure complete denaturation prior to hybridisation. After the hybridization, which occurs during a 20 minutes slow cooling step, the flowcell was washed for 5 minutes with a wash buffer (0.3×SSC/0.1% Tween).
A typical amplification process is presented in Table 1, which details the flow volumes per channel.
Template Hybridization and 1st Extension
Pump Hybridization pre-mix
Pump Hybridization mix
Stop flow and hold T
Pump wash buffer
Pump amplification pre-mix
Pump amplification mix
cool to room temperature
Pump Bst mix
Stop flow and hold T
Pump wash buffer
Details are as follows: Hybridisation pre mix (buffer)=5×SSC/0.1% Tween; Hybridisation mix=0.1 M hydroxide DNA sample, diluted in hybridisation pre mix; Wash buffer=0.3×SSC/0.1% Tween; Amplification pre mix=2 M betaine, 20 mM Tris, 10 mM Ammonium Sulfate, 2 mM Magnesium sulfate, 0.1% Triton, 1.3% DMSO, pH 8.8; Amplification mix=2 M betaine, 20 mM Tris, 10 mM Ammonium Sulfate, 2 mM Magnesium sulfate, 0.1% Triton, 1.3% DMSO, pH 8.8 plus 200 μM dNTP's and 25 units/mL of Taq polymerase (NEB Product ref M0273L); Bst mix=2 M betaine, 20 mM Tris, 10 mM Ammonium Sulfate, 2 mM Magnesium sulfate, 0.1% Triton, 1.3% DMSO, pH 8.8 plus 200 μM dNTP's and 80 units/mL of Bst polymerase (NEB Product ref M0275L)
Step 2: Blocking Extendable 3′-OH Groups
To prepare the blocking pre-mix, 1530 μL of water and 170 μL of 10× blocking buffer (NEB buffer 4; product number B7004S) are mixed for a final volume of 1700 μL. To prepare the blocking mix, 1065.13 μL of blocking pre-mix, 21.12 μL of 125 μM ddNTP mix, and 13.75 μL of TdT terminal transferase (NEB; part no M0252S) are mixed for a final volume of 1100 μL.
To block the nucleic acid within the clusters formed in the flow cell channels, the computer component of the instrumentation flows the appropriate blocking buffer through the flow cell, and controls the temperature as shown in the exemplary embodiments below in Table 3.
Pump Blocking mix
Stop flow and
Blocking mix and
(20 + 180)
Pump wash buffer
To prepare the linearization mix, 1429 μL of water, 64 mg of sodium periodate, 1500 μL of formamide, 60 μL of 1M Tris pH8, and 6011.4 μL of 3-aminopropanol are mixed for a final volume of 3 mL. The periodate is first mixed with the water while the Tris is mixed with the formamide. The two solutions are then mixed together and the 3-aminopropanol is added to that mixture.
To linearize the nucleic acid within the clusters formed within the flow cell channels, 300 μL per channel of linearisation mix is flowed in at 15 μL/minutes at 20° C.; followed by 75 μL of water at the same flow rate.
To prepare the primer mix, 895.5 μL of hybridization buffer and 4.5 μl of sequencing primer (100 μM) are mixed to a final volume of 900 μL. The sequence of the sequencing primer used in the first reaction was:
(SEQ ID NO. 57)
To denature the nucleic acid within the clusters and to hybridize the sequencing primer, the following reagents are flowed through the cell as shown in Table 4:
Pump 0.1 M NaOH
Pump Primer mix
Hold at 60 C.
Pump wash buffer
Sequencing of the clusters from the above illustrative protocol was carried out using modified nucleotides prepared as described in International patent application WO 2004/018493, and labeled with four spectrally distinct fluorophores, as described in U.S. application No. 60/801,270; filed May 18, 2006. Sequencing of clusters is described in more detail in patent WO06064199. The contents of the above-listed three documents are incorporated herein by reference in their entireties.
A mutant 9°N polymerase enzyme (an exo-variant including the triple mutation L408Y/Y409A/P410V and C223S) was used for the nucleotide incorporation steps.
Incorporation mix, Incorporation buffer (50 mM Tris-HCl pH 8.0, 6 mM MgSO4, 1 mM EDTA, 0.05% (v/v) Tween −20, 50 mM NaCl) plus 110nM YAV exo-C223S, and 1 μM each of the four labeled modified nucleotides, was applied to the clustered templates, and heated to 45° C.
Templates were maintained at 45° C. for 30 minutes, cooled to 20° C. and washed with Incorporation buffer, then with 5×SSC/0.05% Tween 20. Templates were then exposed to Imaging buffer (100 mM Tris pH7.0, 30 mM NaCl, 0.05% Tween 20, 50 mM sodium ascorbate, freshly dissolved). Templates were scanned in 4 colors at room temperature. Templates were then exposed to sequencing cycles of Cleavage and Incorporation as follows:
Cleavage: Prime with Cleavage buffer (0.1M Tris pH 7.4, 0.1M NaCl and 0.05% Tween 20), 125 μL/channel; 60 μL/minutes.
Incorporation: Prime with Incorporation buffer, 125 μL/channel; 60 μL/minutes, Heat to 60° C.
Incorporation mix, 25 μL/channel; 60 μL/minutes, every 4 minutes.
Repeat the process of Incorporation and Cleavage for as many cycles as required.
Incorporated nucleotides were detected using a Total Internal Reflection based fluorescent CCD imaging apparatus described in “Systems and Devices for Sequence by Synthesis Analysis,” U.S. Ser. No. 60/788,248, filed Mar. 31, 2006.
The first sequencing primer can be removed, and a second one applied using the same protocol as described in Example 7. The sequence of the second sequencing primer was as follows:
(SEQ ID NO. 58)
The sequencing cycles described in Example 8 can be repeated to sequence the tag. In this case, only three cycles of sequencing were performed to analyse the tag. The data in
Step 1) Grafting Primers onto Surface of SFA Coated Chip
An SFA coated chip is placed onto a modified MJ-Research thermocycler and attached to a peristaltic pump. Grafting mix consisting of 0.5 μM of a forward primer and 0.5 μM of a reverse primer in 10 mM phosphate buffer (pH 7.0) is pumped into the channels of the chip at a flow rate of 60 μl/minutes for 75 s at 20° C. The thermocycler is then heated to 51.6° C., and the chip is incubated at this temperature for 1 hour. During this time, the grafting mix undergoes 18 cycles of pumping: grafting mix is pumped in at 15 μl/minutes for 20 s, then the solution is pumped back and forth (5 s forward at 15 μl/minutes, then 5 s backward at 15 μL/minutes) for 180 s. After 18 cycles of pumping, the chip is washed by pumping in 5×SSC/5 mM EDTA at 15 μl/minutes for 300 s at 51.6° C. The thermocycler is then cooled to 20° C.
The primers are typically 5′-phosphorothioate oligonucleotides incorporating any specific sequences or modifications required for cleavage. Their sequences and suppliers vary according to the experiment for which they are to be used, and in this case were complementary to the 5′-ends of the template duplex. The DNA sequence used in this process was the pool of the twelve libraries, which have ends complementary to the grafted primers. The library mix was denatured using sodium hydroxide treatment followed by snap dilution as described.
The grafted primers contain a sequence of T bases at the 5′-end to act as a spacer group to aid linearisation and hybridization. The sequences of the three primers grafted to the chip are as follows:
(SEQ ID NO. 59)
where U = 2-deoxyuridine;
(SEQ ID NO. 60)
where Goxo = 8-oxoguanine).
Step 2) Preparation of Clusters by Isothermal Amplification:
The DNA sequence used in the amplification process is the mixture of the twelve libraries prepared in Example 1, which have ends complementary to the grafted primers. The duplex DNA (1 nM) is denatured using 0.1 M sodium hydroxide treatment followed by snap dilution to the desired 0.2-2 pM ‘working concentration’ in ‘hybridization buffer’ (5×SSC/0.1% Tween).
Surface amplification was carried out by isothermal amplification using a commercially available Solexa/Illumina cluster station as described in WO08002502. The cluster station is essentially a hotplate and a fluidics system for controlled delivery of reagents to a flow cell.
The single stranded template (denatured as indicated above) is hybridised to the grafted primers immediately prior to the amplification reaction, which thus begins with an initial primer extension step rather than template denaturation. The hybridization procedure begins with a heating step in a stringent buffer to ensure complete denaturation prior to hybridisation. After the hybridization, which occurs during a 20 minute slow cooling step, the flowcell was washed for 5 minutes with a wash buffer (0.3×SSC/0.1% Tween).
During template hybridization and first extension, a number of solutions/buffers are typically employed, e.g., a solution comprising the DNA samples, a hybridization buffer (5×SSC/0.1% Tween), a wash buffer (0.3×SSC/0.1% Tween), a 2M sodium hydroxide solution, a cluster buffer (200 mM Tris, 100 mM Ammonium Sulfate, 20 mM Magnesium sulfate, 1% Triton, 1.3% DMSO, pH 8.8); an amplification additive (5 M betaine), DNA polymerase, and 10 mM dNTP mix.
To prepare the hybridization mixes, a 0.2 ml strip sample tube and the hybridization buffer are pre-chilled. Using 1.7 ml Eppendorf tube(s), the DNA template(s) are then diluted to 1 nM in buffer EB (Qiagen). 1 μL of 2 M NaOH is added to 19 μL of template, vortexed briefly and incubated for 5 minutes at room temperature to denature the DNA template into single strands. The denatured DNA is diluted to working concentration (0.2-2 pM) in pre-chilled hybridization buffer (e.g. for 1 mL of 1 pM Hybridization mix, 1 μL of denatured DNA is diluted into 1 mL of pre-chilled hybridization buffer). The volume required depends on the number of channels used—at least 120 μL of hybridization mix per channel is optionally used. Thus, 1 mL of hybridization mix is enough for 8 channels. The samples are vortexed briefly, spun down and aliquoted into the pre-chilled 0.2 ml strip tubes (with no bubbles in the bottom of the tubes) and used immediately.
To prepare the Amplification pre-mix (of sufficient volume for the first extension and 35 cycles of isothermal amplification), 35 mL of H20 (MilliQ), 7 mL of Cluster buffer (200 mM Tris, 100 mM Ammonium Sulfate, 20 mM Magnesium sulfate, 1% Triton, 1.3% DMSO, pH 8.8), and 28 mL of Amplification additive (5 M betaine solution) are mixed to achieve a final volume of 70 mL.
To prepare the first extension Taq mix, 780 μL of Amplification pre-mix, 16 μL of 10 mM dNTPs, and 4 μL of Taq DNA polymerase are mixed together for a final volume of 800 μl.
A typical amplification process is detailed in Table 1, which includes the flow volumes per channel, controlled automatically by the computer component of the invention.
TABLE 1 Template hybridization and first extension. Flow T Time rate Pumped V Step Description (° C.) (sec) (μl/min) (μl) 1 Pump Hybridization pre-mix 20 120 60 120 2 Pump Hybridization mix 96 300 15 75 3 Remove bubbles 96 6 100 10 4 Stop flow and hold T 96 30 static 0 5 Slow cooling 96-40 1120 static 0 6 Pump wash buffer 40 300 15 75 7 Pump amplification pre-mix 40 280 15 70 8 Pump amplification mix 40 95 60 95 9 First Extension 74 90 static 0 10 cool to room temperature 20 0 static 0
Isothermal Amplification at 60° C. Using Formamide as Denaturant
The copied DNA can be isothermally amplified into clusters at 60° C. using formamide as a denaturant. The isothermal amplification (including both temperature control and reagent control) is overseen by the computer component. Table 2 gives outlines of exemplary script controls. After the isothermal amplification, and optional washing step occur, the nucleic acid of the clusters is ready to be linearized (see below).
Pump Bst mix
Pump wash buffer
Pump Storage Buffer
Wash buffer = 0.3 × SSC/0.1% Tween
Amplification pre mix = 2 M betaine, 20 mM Tris, 10 mM Ammonium Sulfate, 2 mM Magnesium sulfate, 0.1% Triton, 1.3% DMSO, pH 8.8
Bst mix = 2 M betaine, 20 mM Tris, 10 mM Ammonium Sulfate, 2 mM Magnesium sulfate, 0.1% Triton, 1.3% DMSO, pH 8.8 plus 200 μM dNTPs and 80 units/mL of Bst polymerase (NEB Product ref M0275L)
Storage Buffer = 5X SSC.
Step 3) Preparation of Clusters for First Sequencing Read
The preparation for read one was performed on the Illumina cluster station. All volumes used in the protocol were 95 μl per lane unless otherwise stated. Linearisation of A-type surface immobilised oligonucleotides was achieved by incubation with USER enzyme mix (cocktail of Uracil DNA Glycosylase and Endonuclease VIII, NEB #M5505, 10 U/ml, 10 mM KCl, 20 mM Tris pH 8.8, 10 mM (HN4)2SO4, 2 mM MgSO4, 0.1% Triton X-100, 37° C., 30 minutes). All exposed 3′-OH termini of DNA, either from the extended template or unextended surface oligonucleotides were blocked by dideoxy chain termination using a cocktail of terminal transferase (0.25 U/μl) and a modified polymerase (SBS polymerase as described below) (0.015 mg/ml, 100 μM ddNTP, 50 mM tris, 50 mM NaCl, 6 mM MgSO4, 1 mM EDTA, 0.05% Tween 20). Blocking was achieved in a two stage protocol, initial incubation at 37° C. for 30 minutes followed by a ramping to 60° C. and incubating the flowcell for a further 15 minutes). Linearised and blocked clusters were washed with 0.3×SSC and storage buffer prior to denaturation with 0.1N NaOH. Denatured clusters were neutralised with TE buffer (10 mM Tris pH 8.0, 1 mM EDTA) and washed with storage buffer. The read 1 specific sequencing primer
(SEQ ID NO. 61) (5′-ACACTCTTTCCCTACACGACGCTCTTCCGATC-3′,
0.5 μM in hybridisation buffer) was annealed to the clusters by incubation at 60° C. for 15 minutes, followed by a 0.3×SSC wash at 40° C. (ramp rate 1° C./sec). The flowcell was finally flushed with storage buffer (at 20° C.). Processed flowcells were transferred to the Illumina Genome Analyser for sequencing read 1.
Step 4) Sequencing from the Target Fragment
Sequencing of the clusters from the above illustrative protocol was carried out using modified nucleotides prepared as described in International patent application WO 2004/018493, and labeled with four spectrally distinct fluorophores, as described in PCT application number PCT/GB2007/001770, published as WO07135368. Sequencing of clusters is described in more detail in WO06064199. The contents of the above-listed documents are incorporated herein by reference in their entireties.
A mutant 9°N polymerase enzyme (an exo-variant including the triple mutation L408Y/Y409A/P410V and C223S) (SBS polymerase) was used for the nucleotide incorporation steps.
All processes were conducted as described in the Illumina Genome Analyser operating manual. The flowcell was mounted to the analyser, primed with sequencing reagents: position #1=incorporation mix (1 μM dNTP mix, 0.015 μg/ml SBS polymerase, 50 mM Tris pH 9.0, 50 mM NaCl, 6 mM MgSO4, 1 mM EDTA, 0.05% Tween 20); position # 2=spare (MilliQ water only); position # 3=scan mix (100 mM Tris pH 7.0, 50 mM sodium acsorbate); position #4=High salt wash (5×SSC, 0.05% Tween 20); position # 5=incorporation buffer (50 mM Tris pH 9.0, 50 mM NaCl, 1 mM EDTA, 0.05% Tween 20); position #6=cleavage mix (100 mM TCEP, 100 mM Tris pH 9.0, 100 mM NaCl, 50 mM sodium ascorbate, 0.05% Tween 20); position #7=cleavage buffer (100 mM Tris pH 9.0, 100 mM NaCl, 0.05% Tween 20); position #8=spare (single reads) or connected to PE module outlet (paired read experiments). Flowcells were sequenced using standard sequencing recipes for either 27- or 37-cycle experiments. Data was analysed using the standard analysis pipeline.
Incorporation: Prime with Incorporation buffer, 125 μL/channel; 60 μL/minutes, Heat to 60° C.
Cleavage: Prime with Cleavage buffer (0.1M Tris pH 7.4, 0.1M NaCl and 0.05% Tween 20), 125 μL/channel; 60 μL/minutes.
Repeat the process of Incorporation and Cleavage for as many cycles as required.
Incorporated nucleotides were detected using the Illumina genome analyzer, a Total Internal Reflection based fluorescent CCD imaging apparatus described in “Systems and Devices for Sequence by Synthesis Analysis,” U.S. Ser. No. 60/788,248, filed Mar. 31, 2006 and corresponding PCT application PCT/U.S.07/07991, published as WO07123744, the contents of which are incorporated herein by reference in their entireties.
Step 5) Sequencing of the Tag
Following the successful completion of sequencing the first read on the Genome Analyser, flowcells remained mounted and were prepared for tag sequencing in situ, using the Illumina Paired End module. Temperature control was achieved by using the Genome Analyser peltier. All flow rates were 60 μl/min and 75 μl per lane unless otherwise stated. Clusters were denatured with 0.1 M NaOH to remove the extended sequencing primer from read 1. Hybridisation of the tag sequencing primer
(SEQ ID NO. 62) (5′-GATCGGAAGAGCACACGTCTGAACTCCAGTCAC-3′),
0.5 μM in hybridisation buffer) as described for read 1. Sequencing of the tag was performed on the Illumina Genome Analyser.
Step 6) Preparation of the Clusters for the Paired Sample Read
Following the successful completion sequencing of two reads on the Genome Analyser, flowcells remained mounted and were prepared for paired read 2 in situ, using the Illumina Paired End module. Temperature control was achieved by using the Genome Analyser peltier. All flow rates were 60 μl/min and 75 μl per lane unless otherwise stated. Clusters were denatured with 0.1 M NaOH to remove the extended sequencing primer from the tag sequencing. Clusters were 3′-dephosphorylated using T4 polynucleotide kinase (Invitrogen #18004-010, 200 U/ml, 50 mM imidazole pH 6.4, 12 mM MgCl2, 70 μM ADP, 1 mM 2-mercaptoethanol, 37° C., 30 minutes), prior to re-synthesis of the A-strand achieved using 15 cycles of 60° C. isothermal amplification (same reagents and conditions as described for cluster creation except conducted at 30 μl/min). Clusters were washed before and after resynthesis with 0.3×SSC (150 μl and 245 μl respectively). Linearisation of the B-strand of the re-synthesised clusters was achieved by the excision of 8-oxoguanine from the B-type oligo using Fpg (formamidopyrimidine DNA glycosylase, NEB #M0240, 80 U/ml, 10 mM Bis Tris propane pH 7.0, 10 mM MgCl2, 1 mM dithiothreitol, 37° C., 30 minutes). Blocking was performed as described for read 1 using the same blocking cocktail. Linearised and blocked clusters were denatured prior to hybridisation of the read 2 specific sequencing primer
(SEQ ID NO. 63) (5′-GTGACTGGAGTTCAGACGTGTGCTCTTCCGATC-3′),
0.5 μM in hybridisation buffer) as described for read 1. Read 2 of the processed flowcells was subsequently sequenced on the Illumina Genome Analyser.
Data generated from the 12 samples is shown in
While the foregoing invention has been described in some detail for purposes of clarity and understanding, it will be clear to one skilled in the art from a reading of this disclosure that various changes in form and detail can be made without departing from the true scope of the invention. For example, all the techniques and apparatus described above may be used in various combinations. All publications, patents, patent applications, or other documents cited in this application are incorporated by reference in their entirety for all purposes to the same extent as if each individual publication, patent, patent application, or other document were individually indicated to be incorporated by reference for all purposes.
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|U.S. Classification||435/6.12, 435/6.1, 435/6.11|
|International Classification||C12Q1/68, C12P19/34|
|Jul 20, 2009||AS||Assignment|
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